The netrin receptor DCC focuses invadopodia-driven basement membrane transmigration in vivo

Basement membrane is a thin, dense, extracellular matrix that surrounds most tissues, acting as a physiological barrier to maintain tissue homeostasis (Kalluri, 2003). Several cell types, including those undergoing epithelial–mesenchymal transition, migrating neural crest and muscle, implanting trophoblast, and leukocytes have the specialized ability to breach and cross basement membrane barriers (Hughes and Blau, 1990; Poelmann et al., 1990; Sato et al., 2003; Wang et al., 2006; Nakaya et al., 2008). Acquisition of cell-invasive activity is also critical for the deadly spread of most cancers (Valastyan and Weinberg, 2011). Traversing basement membrane requires several distinct cellular processes, including matrix adhesion, basement membrane breaching and removal, passage through the basement membrane barrier, and integration into the neighboring tissue. The difficulty of visualizing and experimentally examining cell–basement membrane interactions during invasion in vivo has greatly limited our understanding of how cells coordinate these tasks during basement membrane transmigration (Rowe and Weiss, 2008; Madsen and Sahai, 2010).

Anchor cell (AC) invasion in Caenorhabditis elegans is a simple in vivo model of basement membrane transmigration that allows visual access to the invasive cell–basement membrane interface (Sherwood and Sternberg, 2003; Hagedorn and Sherwood, 2011). During normal hermaphrodite development, the uterine AC breaches the basement membrane separating the uterine and vulval epithelium to establish the initial connection between these tissues. The timing of AC invasion is highly stereotyped and is tightly coordinated with the division of the underlying vulval cells (Fig. S1 A). Both the integrin heterodimer INA-1/PAT-3 and the netrin receptor UNC-40 (DCC) localize to the cell membrane of the AC in contact with the basement membrane and are thought to promote invasion by regulating F-actin polarized toward the AC–basement membrane interface (Hagedorn et al., 2009; Ziel et al., 2009). How these pathways specifically mediate F-actin dynamics and facilitate basement membrane breaching and transmigration is unclear.

By developing methods for time-lapse microscopy of AC invasion, we identify here highly dynamic, integrin-dependent, F-actin–based structures that breach the basement membrane. These protrusive, F-actin–rich foci share molecular composition and activity with invadopodia, invasive structures identified in transformed and highly invasive cancer cells in vitro (David-Pfeuty and Singer, 1980; Chen, 1989; Murphy and Courtneidge, 2011). Many invadopodia form and turn over within the AC before invasion, but usually only one penetrates the basement membrane and then gives rise to a stable protrusion that invades the vulval tissue. We find that the netrin receptor UNC-40 (DCC) is highly enriched at sites of basement membrane breach and within the invasive protrusion. Animals lacking UNC-40 fail to form an invasive protrusion and have persistent invadopodia, multiple basement membrane breaches, and inefficient basement membrane removal. Using optical highlighting of basement membrane components, we show that this UNC-40–dependent invasive protrusion accelerates basement membrane removal in part by physically displacing this barrier. Together, these studies reveal an UNC-40 (DCC)–dependent mechanism that ensures focused invasion at nascent sites of basement membrane breach.

To investigate how the AC crosses the basement membrane, we developed methods combining nontoxic anesthesia, multidimensional time-lapse microscopy, and quantitative image analysis to view the invasive cell–basement membrane interface in real time (Fig. 1 A and Video 1). Actin dynamics and basement membrane integrity were simultaneously visualized using animals expressing AC-specific F-actin probes (cdh-3 > mCherry::moeABD or cdh-3 > Lifeact::GFP) and functional transgenes for the basement membrane components laminin (laminin::GFP) and type IV collagen (emb-9::mCherry; Ziel et al., 2009; Ihara et al., 2011). Beginning 3 h before invasion, F-actin within the AC was polarized toward the basement membrane and organized into highly dynamic punctate structures with lifetimes on a timescale of minutes (Fig. 1 B; Fig. S1, B and E; and Video 1). Quantitative image analysis revealed these F-actin foci had a mean diameter of 1.00 ± 0.38 µm (±SD, n = 8,182 structures from 10 animals) and a median lifetime of 45 s (ranging from 15 to 930 s). Before invasion, nascent structures formed at a steady rate of 2.8 ± 0.4 structures per minute and there were on average 11 ± 3 structures present (Fig. S1 E).

F-actin–rich, matrix-degrading membrane structures called invadopodia have been identified in a variety of malignant cancer cell lines, as well as transformed fibroblasts and zebrafish epithelial cells (Linder et al., 2011; Murphy and Courtneidge, 2011; Seiler et al., 2012). Invadopodia are defined by their localization at sites of extracellular matrix removal, association with invasive cells, and highly protrusive nature (Linder et al., 2011; Murphy and Courtneidge, 2011). To determine if the F-actin structures in the AC were similar to invadopodia, we first examined their relationship to the basement membrane. High-resolution lateral perspective imaging at single time points revealed that these F-actin foci were highly protrusive, often appearing to depress the underlying basement membrane (Fig. 1 C and see Materials and methods). Time-lapse imaging from the ventral perspective showed that these structures always presaged and then localized to the site of the initial visible basement membrane breach (Fig. 1, D and E; Fig. S1 C; and Video 2; n = 8/8 animals observed). Strikingly, in most cases only one or two basement membrane breaches were made within a narrow 15-min period during the mid-to-late L3 larval stage (n = 6/12 animals had one breach, 3/12 two, 1/12 three, and 2/12 four; Fig. 2 C), usually occurring within the central region of the AC’s footprint (Fig. S1 D). The protrusive nature of these F-actin structures and their localization at sites of basement membrane breach strongly suggest these are in vivo invadopodia.

Although there is no single molecular marker of invadopodia, many actin regulators are known to associate with these structures (Saltel et al., 2011; Klemke, 2012). We recently demonstrated that several actin regulators that are connected with invadopodia in vitro localize to the invasive cell membrane of the AC before invasion (Ziel et al., 2009). These include the Ena/VASP orthologue UNC-34, the phospholipid phosphatidylinositol 4,5-bisphosphate (PI(4,5)P₂), and the Rac GTPases MIG-2 and CED-10 (Nakahara et al., 2003; Philippar et al., 2008). Quantitative analysis revealed that all of these molecules colocalized with the F-actin foci in the AC (Fig. S2 A). Importantly, the cell membrane marker FM1-43 was found uniformly in the AC’s invasive cell membrane, indicating that these structures are specific molecular enrichments as opposed to general accumulations of membrane (Fig. S2 B). In vitro studies have also demonstrated that engagement of the extracellular matrix receptor integrin is a prerequisite for invadopodia formation (Destaing et al., 2010). Notably, RNAi-mediated depletion of the integrin heterodimer INA-1/PAT-3, the sole integrin expressed in the AC (Hagedorn et al., 2009), dramatically reduced F-actin structure formation (Fig. S2 C; n = 8/8 animals). Collectively our results offer compelling evidence that these F-actin foci are AC-invadopodia.

To determine how AC-invadopodia contribute to basement membrane transmigration, we followed the fate of the invadopodia that breached the basement membrane. We found that soon after breaching, an infiltrated invadopodium matured into an invasive process that expanded through the basement membrane and into the underlying vulval tissue (over an ∼1-h time frame and at a rate of 1.08 ± 0.42 µm³/min; Fig. 2, A and C; and Video 3; n = 13 animals observed). At the onset of protrusion extension, AC-invadopodia ceased to form and F-actin enriched in the expanding cellular process (Video 4; n = 18/18 animals). As the invasive protrusion expanded ventrally, the corresponding breach widened radially until the completion of invasion (rate of 0.20 ± 0.06 µm²/min; Fig. 2, B and C; and Video 4; n = 13 animals). During this time the neck of the invading cellular protrusion maintained contact with the basement membrane. In instances where two invadopodia breached, only one of these developed into a protrusion (n = 3/3 cases observed) that invaded the vulval tissue and widened a single large gap in the basement membrane (Fig. 2 B). Thus, when more than one invadopodia penetrates the basement membrane, a competitive interaction occurs between these sites, which results in a single invasive protrusion forming. Similar results were obtained examining the basement membrane component type IV collagen. Together, these results indicate that AC-invadopodia usually breach the basement membrane at only one or two sites and that only one invasive protrusion forms that directs invasion through the basement membrane and into the underlying vulval cells.

The observation that hundreds of invadopodia form and turn over before invasion, but only one or two basement membrane breaches form, suggested that a molecular signal might specify or reinforce the site of basement membrane breach. We have previously shown that UNC-6 (netrin) secreted from the ventral nerve cord (VNC) adjacent to the vulval cells promotes AC invasion, in part, by targeting its receptor UNC-40 (DCC) to the invasive cell membrane (Fig. S1 A; Ziel et al., 2009). To determine whether netrin signaling might select a site for basement membrane breach, we examined the localization of a functional GFP fusion to the netrin receptor UNC-40 (DCC). UNC-40::GFP was present throughout the invasive cell membrane before invasion, but did not tightly colocalize with the AC-invadopodia (Fig. S3 A). Consistent with this localization, loss of unc-40 did not alter invadopodia formation or their dynamics before invasion (Fig. S3, B and C). Strikingly, however, UNC-40 enriched at nascent basement membrane breaches (Fig. 3, A and B; and Video 5). This enrichment in UNC-40 occurred ∼20 min before the formation of a visible basement membrane break, suggesting UNC-40 might promote basement membrane opening (Fig. 3 B). Supporting this notion, we found that in unc-40 (e271) mutant animals the initial visible breach was delayed by ∼1.5 h (Fig. 3 C). We conclude that UNC-40 (DCC) does not regulate invadopodia formation or dynamics, but has a role in promoting visible basement membrane gap formation.

The specific localization of UNC-40::GFP at sites of basement membrane breach led us to investigate the role of UNC-40 in building the stable invasive protrusion that forms shortly after basement membrane penetration. Notably, UNC-40::GFP continued to further enrich during basement membrane opening and localized to the invasive process that extended into the vulval tissue (Fig. 3 B and Fig. S4 A). This specific enrichment suggested that UNC-40 might promote basement membrane opening and the transition of invadopodia into an invasive process that switches the invasive state of the AC from invadopodia-driven basement membrane breaching to invasive protrusion-directed basement membrane crossing. Consistent with this idea, though delayed in breaching, in unc-40 mutant animals the invadopodia persisted after visible basement membrane gaps were formed, often resulting in excessive breaches (as many as seven; Fig. 4, A and B; and Fig. S4 B). Furthermore, we never observed the formation of a significant invasive protrusion after loss of unc-40 (Fig. 4, C and D). The hole in the basement membrane of unc-40 mutant animals widened at half the rate of wild-type animals (Fig. 4, E and F; and Video 6), suggesting that the protrusion is important for basement membrane gap opening. Collectively, these data indicate that UNC-40 mediates a morphogenetic transition that promotes the maturation of an invadopodium into a stable invasive protrusion, which leads to the cessation of further invadopodia formation, invasion into the neighboring vulval tissue, and accelerated basement membrane removal.

We next examined the relationship between UNC-40 and UNC-6 during invadopodia maturation. UNC-6 is secreted from the VNC adjacent to the vulval cells, and we have previously shown that low, uniform levels of the functional reporter UNC-6::Venus are present in the basement membrane at the time of invasion (Ziel et al., 2009). We found that unc-6 (ev400) mutants displayed a phenotype largely similar to loss of unc-40—there was a delay in basement membrane breaching, a multiple basement membrane hole phenotype, and a complete failure to extend an invasive protrusion through the basement membrane (Fig. 4, A–D). Notably, the multiple basement membrane hole phenotype was more severe in unc-40 mutants, suggesting that this activity is not fully dependent on UNC-6 (Fig. 4 B). Examination of UNC-40::GFP in unc-6 (ev400) mutants also revealed that UNC-40::GFP still enriched at basement membrane breaches (Fig. S4 C). These observations suggest that UNC-6 activates the UNC-40 receptor, but that another mechanism must exist to selectively localize UNC-40 to the site of basement membrane breach.

We next addressed how UNC-40 promotes formation of an invasive protrusion. UNC-40 (DCC) is thought to function in cell migration and axon guidance by recruiting and activating downstream effectors that modulate the actin cytoskeleton (Quinn et al., 2008; Ziel et al., 2009; Lai Wing Sun et al., 2011). We therefore examined the localization of functional GFP-tagged reporters for known UNC-40 effectors to determine if they are recruited to basement membrane breaches like UNC-40. We found that the Ena/VASP orthologue UNC-34 and the Rac orthologue MIG-2 both enriched at the initial basement membrane breach in wild-type animals but that this enhancement in localization was absent in unc-40 mutants (Fig. 5 A and Fig. S4 D). Furthermore, examination of F-actin, the output of these effectors, revealed dynamic and focused formation at the expanding site of breach during protrusion growth with F-actin repeatedly forming and disassembling at the site of breach where UNC-40 was stably localized (Fig. 5, B and C; Video 7; and Video 8). In contrast, in unc-40 mutant animals, dynamic F-actin polymerization was not focused at sites of breach (Fig. 5 C and Video 9). Consistent with these effectors acting downstream of UNC-40 at sites of basement membrane breach, we have previously reported that perturbation of these molecules leads to a delay in AC invasion (Ziel et al., 2009). To determine if these effectors might also mediate invasive protrusion formation, we examined unc-34(e951); mig-2(mu28) double mutant animals. Supporting a role in fostering invasive protrusion growth downstream of UNC-40, we found a complete absence of invasive processes after loss of unc-34 and mig-2 (n = 9/9 animals observed). These results suggest that UNC-40 directs focused F-actin generation through F-actin regulatory proteins at the site of basement membrane breach to direct stable protrusion formation.

We were next interested in understanding how the UNC-40–mediated invadopodia-to-invasive protrusion transition enhances basement membrane removal. During our initial analysis, we noted that the invasive protrusion in wild-type animals remained in continuous contact with the edge of the expanding basement membrane gap (Fig. S5 A). Further, the basement membrane opening was much rounder in wild-type animals versus unc-40 mutants, even in cases where only a single gap was created (Fig. 6, B and C; wild type: circularity = 0.89, n = 15; unc-40(e271): circularity = 0.56, n = 14; P < 0.0001, Student’s t test). Finally, we noticed increased levels of laminin and type IV collagen at the rim of the expanding basement membrane gap in wild-type animals (Fig. S5 B). These observations suggested that the expanding protrusion might speed basement membrane gap opening by physically displacing the basement membrane. Importantly, the AC is known to secrete matrix components during invasion (Sherwood et al., 2005), and so we could not exclude the possibility that this increase was simply a result of new basement membrane deposition. Thus, to directly test whether displacement was occurring we used transgenic animals expressing laminin::Dendra or type IV collagen::Dendra. Dendra is a highly stable, photoconvertible fluorescent protein that changes irreversibly from a green to a red fluorescent state after exposure to low phototoxic, short wavelength light (Gurskaya et al., 2006). To determine if the basement membrane was displaced during invasion, we optically highlighted the basement membrane precisely beneath the AC before invasion using an AC-specific GFP membrane marker (Fig. 6 A). We observed photoconverted laminin::Dendra displaced to the sides of the AC after invasion, nearly doubling the distance between the outer edges of highlighted region (Fig. 6, A and C), indicating that the basement membrane was physically moved. In contrast, control regions of optically highlighted basement membrane adjacent to the AC remained intact and only slightly widened, likely because of diffusion of basement membrane components and growth (the basement membrane beneath the AC widened 1.8- versus 1.2-fold in control regions; Fig. 6, A and C; Ihara et al., 2011). To quantify the amount of the basement membrane displaced during invasion, we photoconverted all of the laminin:Dendra in the vicinity of the AC before invasion. An estimate of the percentage of basement membrane displaced was then calculated based on the additional fluorescence intensity at the edges of the expanding gap (see Materials and methods; Fig. 6, B and C). Using this approach we determined that a mean of 26% of the basement membrane was physically displaced during AC invasion in wild-type animals (Fig. 6, B and C; n = 27). Importantly, this estimate likely underrepresents basement membrane displacement, as our method for quantification can only measure basement membrane that accumulated at the edge of the expanding gap and does not account for basement membrane that might be stretched thin or moved beyond the boundary of the basement membrane gap. Similar results were obtained with type IV collagen::Dendra (Fig. S5 C). In unc-40 (e271) mutants, where an invasive protrusion is never formed, we observed that only 8% of the basement membrane was displaced during gap formation (n = 14; P = 0.0012; Fig. 6, B and C), supporting the notion that the invasive protrusion in wild-type animals accelerates basement membrane removal by displacement. The finding that some laminin and type IV collagen still accumulate at the edges of basement membrane openings in unc-40 mutants suggests that a redundant mechanism might also exist to physically move basement membrane or that basement membrane diffusion may facilitate displacement. We conclude that the invasive protrusion enhances basement membrane crossing, in part, by physically displacing this barrier to clear a path for invasion.

The ability of cells to invade through basement membrane and enter new tissues is critical to many normal morphogenetic processes as well as cancer metastasis. By developing real-time methods to visualize AC invasion in C. elegans, we find that dynamic invadopodia are used to breach the basement membrane. Further, we show that the UNC-40 (DCC) receptor localizes to sites of basement membrane breach and directs the creation of a single large invasive protrusion that displaces basement membrane, guides invasion into the underlying vulval tissue, and leads to the cessation of further invadopodia formation (for a summary, see Fig. 7). Together, our results reveal a key UNC-40–mediated morphogenetic transition that directs invading cells through basement membrane and into neighboring tissues.

To date, invadopodia, defined primarily by their protrusive nature and ability to remodel extracellular matrix, have only been described in metastatic cancer cell lines or transformed cells (Chen, 1989; Linder et al., 2011; Seiler et al., 2012). Using live-cell imaging, we find that basement membrane breaching during AC invasion is mediated by protrusive F-actin–based invadopodia. Although most of the F-actin–based structures within the AC were similar in size and stability (∼1 µm in diameter and lifetime of 45 s; Fig. S1 E), some were consistently outside of this range in dimension and lifetime. Thus, these F-actin foci are likely not all invadopodia and some may be sites of endocytosis and adhesion. Nevertheless, the largely similar dynamics and their striking disappearance shortly after basement membrane breaching offers compelling evidence that many if not most of these structures are bona fide in vivo invadopodia.

Over fifty proteins are known to localize to or regulate invadopodia function in cancer cells (Hoshino et al., 2012; Klemke, 2012). Our initial characterization indicates that the invadopodia in the AC have similar molecular composition to cancer cell invadopodia, including the presence of C. elegans orthologues of vertebrate Rac GTPases and Ena/VASP, as well as the presence of the phospholipid PI(4,5)P₂ (Nakahara et al., 2003; Philippar et al., 2008; Yamaguchi et al., 2010). The AC-invadopodia also share a dependency on integrin activity (Destaing et al., 2010). Additionally, the C. elegans genome encodes orthologues of many additional proteins implicated in invadopodia formation or function, such as the Src and FAK tyrosine kinases, paxillin, the Arp 2/3 complex, the actin nucleation-promoting factor WASP, and matrix metalloproteinases, which may play a similar role in the AC as they do in cancer cells (Saltel et al., 2011; Shaye and Greenwald, 2011; Hoshino et al., 2012; Klemke, 2012). One notable exception, however, is the absence of the actin nucleation–promoting factor cortactin in C. elegans, a key regulator of invadopodia in several cancer cell lines (Artym et al., 2006; Ayala et al., 2008; Shaye and Greenwald, 2011). Thus, the AC-invadopodia might have differences in their regulation and composition from cancer cells, or other proteins may compensate for the absence of cortactin in C. elegans.

We have also discovered that soon after an invadopodium penetrates the basement membrane, a large invasive protrusion forms at the site of breach and invades the underlying vulval epithelium. Formation of a stable protrusion is accompanied by the cessation of invadopodia, thus shutting down additional basement membrane breaches and focusing invasion through a single basement membrane gap. Transition to an invasive protrusion likely also stabilizes an invasion site by anchoring a cell to the neighboring tissue. Studies in ex vivo invasion assays have observed single protrusions from invasive cancer cells crossing native basement membrane (Hotary et al., 2006; Schoumacher et al., 2010), consistent with this being a conserved mode of basement membrane invasion. Importantly, we have found that the netrin ligand UNC-6 and its receptor UNC-40 (DCC) mediate this critical switch. UNC-40 selectively enriched at sites where invadopodia first visibly breached the basement membrane, and through activation by UNC-6 and recruitment of effectors, promoted F-actin formation and the construction of an invasive protrusion. Although netrins are well established for their role in mediating axon guidance, cell migration, and epithelial morphogenesis (Lai Wing Sun et al., 2011), they are also proangiogenic factors in vertebrates and promote vascular sprouting through basement membrane (Heissig et al., 2003; Wilson et al., 2006). Further, the netrin-1 ligand is overexpressed in numerous metastatic cancers (Fitamant et al., 2008; Dumartin et al., 2010; Ramesh et al., 2011) and stimulates invasion in pancreatic, colon, glioblastoma, and melanoma cancers assayed in vitro and ex vivo (Rodrigues et al., 2007; Kaufmann et al., 2009; Dumartin et al., 2010; Shimizu et al., 2012). These results suggest that netrin signaling broadly promotes invasion and that netrin might play a conserved role in directing invasive protrusion formation. Surprisingly, evidence in vertebrates and Drosophila melanogaster have suggested that UNC-40 (DCC) receptors may also function as tumor and metastasis suppressors, perhaps through their role in maintaining epithelial and endothelial cell survival in the presence of netrin ligands and promoting apoptosis in their absence (VanZomeren-Dohm et al., 2011; Castets et al., 2012; Krimpenfort et al., 2012). These observations indicate that in different cell contexts DCC may function as either a tumor suppressor or enhancer during cancer progression.

The expression of matrix-degrading proteases and the presence of type IV collagen degradation products at sites of invasion in human carcinomas have supported the widely held idea that basement membrane barriers are overcome through proteolytic dissolution by invasive cells (Garbisa et al., 1980; Xu et al., 2001; Sherwood et al., 2005; Hotary et al., 2006; Overall and Kleifeld, 2006; Page-McCaw et al., 2007). Intriguingly, studies of epithelial and carcinoma cells have shown that these cells physically compress and displace basement membrane components in vitro (Rabinovitz et al., 2001), a cellular behavior that might also contribute to creating gaps in endogenous basement membrane. Using optical highlighting, we found that the AC physically displaces the basement membrane components laminin and type IV collagen during basement membrane gap formation. Our quantitative analysis suggests that at least 26% of basement membrane is displaced during invasion. We think this is an underestimate, as our methods for determining displacement cannot account for basement membrane that stretches or moves beyond the basement membrane gap boundary. Notably, we previously found that the matrix metalloproteinase zmp-1 is expressed in the AC during invasion, where it may act redundantly with other proteases that promote basement membrane removal (Sherwood et al., 2005). These results offer a new model to account for cell invasion through basement membrane barriers, where the combined action of proteases and physical forces coordinate basement membrane removal. Collectively our studies indicate that basement membrane transmigration is not a simple process of basement membrane dissolution, but rather a progressive series of highly regulated and interlinked steps that act to mediate breaching, removal, and passage through basement membrane barriers.

Culturing and handling of C. elegans was done as previously described (Brenner, 1974). Wild-type animals were strain N2. In the text and figures, we designated linkage to a promoter with a greater than symbol (>) and used a double colon (::) for linkages that fuse open reading frames. The following alleles and transgenes were used in this study: qyIs61[cdh-3 > GFP::UNC-34], qyIs242[cdh-3 > Lifeact::GFP], qyIs46[emb-9::mCherry], qyIs221[cdh-3 > GFP::CED-10], qyIs219[cdh-3 > GFP::PLCδ^PH], qyIs220[cdh-3 > GFP::MIG-2], qyIs67[cdh-3 > UNC-40::GFP], qyIs127[laminin::mCherry], qyIs166[cdh-3 > GFP::CAAX]; LGI, unc-40(e271); LGII, qyIs23[cdh-3 > mCherry::PLCδ^PH]; LGIII, unc-119(ed4); LGIV, qyIs10[laminin::GFP]; LGV, qyIs50[cdh-3 > mCherry::moeABD]; and LGX, qyIs7[laminin::GFP], unc-6(ev400), qyIs24[cdh-3 > mCherry::PLCδ^PH], and qyIs66[cdh-3 > UNC-40::GFP].

Images were acquired using a camera (EM-CCD; Hamamatsu Photonics) and a spinning disk confocal microscope (CSU-10; Yokogawa) mounted on a microscope (AxioImager; Carl Zeiss) with a Plan-APOCHROMAT 100×/1.4 oil differential interference contrast objective and controlled by iVision software (Biovision Technologies). Acquired images were processed using ImageJ 1.40g and Photoshop (CS3 Extended; Adobe). 3D reconstructions were built from confocal z-stacks, analyzed, and exported as .mov files using IMARIS 7.4 (Bitplane, Inc.). Figures and graphs were constructed using Illustrator (CS3 Extended; Adobe). Videos were annotated using Photoshop. Quantitative analyses of AC-invadopodia, invasive protrusion, or basement membrane breach formation was done using either ImageJ, Imaris, or both. To be as consistent as possible isosurface renderings, built in place of polymerized F-actin, were used to determine a threshold for assigning the spots that were used to quantify AC-invadopodia dynamics. For time-lapse microscopy, worms were anesthetized in 0.2% tricaine and 0.02% levamosile in M9 and then transferred to 5% noble agar pads, sealed with VALAP, and imaged at 23°C. Capturing the AC-invadopodia structures that presaged the initial basement membrane breach required ventral view time-lapse imaging. Although AC-invadopodia could be observed to depress the basement membrane in single time point lateral view images, we were unable to resolve whether the structures that presaged the initial breach repeatedly depressed the basement membrane.

RNAi targeting pat-3 was delivered by feeding worms Escherichia coli expressing double-stranded RNA. To avoid embryonic lethality, synchronized L1-arrested larvae were grown for 5 h on regular OP50 bacteria in the absence of RNAi. These worms were then transferred to bacteria expressing pat-3 double-stranded RNA. The empty RNAi vector L4440 was used as a negative control. The RNAi vector was sequenced to verify correct insert.

Lifeact::GFP was amplified from pJWZ73, and then linked by PCR fusion to the cdh-3 > promoter. MIG-2 and CED-10 were both amplified from N2 genomic DNA and then linked to a cdh-3 > GFP amplicon by PCR fusion. The PLCδ^PH domain was amplified from pAA173, cloned into pBsSK at the C-terminus of GFP and then linked to the cdh-3 > promoter and unc-54 3′UTR using a three-step PCR fusion. GFP::CAAX was amplified from pSA129, and then linked by PCR fusion to the cdh-3 > promoter. Constructs were coinjected with ∼50 ng/µl unc-119 rescue DNA, ∼50 ng/µl pBsSK, and ∼50 ng/µl EcoRI cut salmon sperm DNA into unc-119(ed4) hermaphrodites. Stably expressed extrachromosomal lines were established and selected lines were integrated by gamma irradiation. See Tables S1 and S2 for primer sequences used and transgenic strains generated.

To visualize the plasma membrane of the AC we used the lipophilic dye FM1-43, which fluoresces green when incorporated into the outer leaflet of the plasma membrane.

Approximately 25 wild-type N2 worms at the early L3 larval stage were transferred to 25 µl of a 0.5 mM FM1-43 dye in M9 in a well of a glass spot plate. The spot plate was covered with parafilm and placed in the dark for 1 h. After incubation, worms were allowed to destain on OP50 food plates for an additional hour. Worms were mounted on 5% noble agar pads containing 0.01 M sodium azide and imaged using a spinning disc confocal and 488-nm laser.

Defined regions of laminin::Dendra and type IV collagen::Dendra were photoconverted using a confocal microscope (LSM 510; Carl Zeiss) equipped with a 63× objective, scanning regions of interest with a 405-nm laser at 1 mW power for 30 s. After photoconversion, images were captured using a spinning disc confocal or an AxioImager microscope. Animals were recovered from the agar pad, allowed to develop at 20°C for the specified amount of time, and then reimaged. The fold change in width of the optically highlighted regions was measured using ImageJ 1.40g. Quantification of percent displacement was done by photoconverting all of the basement membrane within a 15-µm radius of the AC, recovering the worms for 2–3 h, and then reimaging from the ventral perspective. Sum projections of confocal z-stacks were then analyzed using ImageJ 1.40g software and the method described in Fig. 6 B. Measurements of circularity were performed by tracing the boundary of single basement membrane breaches in ImageJ and calculated as 4π(area/perimeter²).

All statistical analysis was performed in JMP version 9.0 (SAS Institute), using either a two-tailed unpaired Student’s t test or nonparametric Wilcoxon rank-sum test. Figure legends specify when each test was used.

Online supplemental material includes five figures, nine videos corresponding to the time-lapse data presented in the main text figures, and two tables, Table S1 for primer sequences and Table S2 for extrachromosomal arrays and integrated strains. Additional data are available in the JCB DataViewer at http://dx.doi.org/10.1083/jcb.201301091.dv.

We are grateful to the Duke University Light Microscopy Core Facility and P. Maddox for advice and reagents, to the Caenorhabditis Genetic Center for providing strains, to the staff at Bitplane, Inc. (Imaris) for technical support, and to L. Kelley and L. Lilley for comments on the manuscript.

This work was supported by The Pew Scholars Program in the Biomedical Sciences and by National Institutes of Health grants GM079320 and GM100083 to D.R. Sherwood.